Sucrose Preference Test to Measure Stress-induced Anhedonia    

Materials and Reagents

1. Sipper caps, composed of 2.5 cm straight stainless steel sipper tubes (VWR International, catalog number: 10718-330 ) inserted into rubber stoppers (VWR International, catalog number: 59581-287 )
   
2. 50 ml conical centrifuge tubes (VWR International, catalog number: 89039-656 )
   
3. Adult (7 weeks or older) mice (C57BL/6J) (The Jackson Laboratory)
   Note: Alternate strains and ages of mice may also be used. Mice are housed singly, in an environment with controlled temperature (around 23 °C) and humidity under a 12-12 h light-dark cycle with food and water ad libitum. See Animal considerations in Notes for more details.
   
4. Sucrose (crystals)
   
5. Reverse osmosis (RO) filtered water
   Note: Alternatively substitute with the mouse’s normal drinking water.
   

Equipment

1. Mouse caging
   
   1. Polycarbonate tubs (Mouse Cage; 7 ½ in W x 11 ½ in L x 5 in H) (Ancare) with standard woodchip mouse bedding (NORTHEASTERN PRODUCTS CORP., Aspen Chip)
      Note: Standard cage changes are allowed during the acclimation period (see below), however it is recommended to avoid cage changes during the period of data collection (Procedure steps 2-5) to prevent leakage. Leakage should be avoided to reduce undesired variability.
      
   2. Stainless steel wire cage lid (Ancare, model: N10SSR Mouse Lid )

Procedure

1. Single house mice in proper mouse caging (see Equipment) under controlled conditions (see Materials and Reagents). Conditions should comply with the Guide for the Care and Use of Laboratory Animals, 8^th ed. (https://grants.nih.gov/grants/olaw/Guide-for-the-Care-and-use-of-laboratory-animals.pdf). Allow mice to acclimate for 7 d under these conditions.
   
2. Setup 2-bottle choice test for baseline conditions (Figure 1).
   
   1. Fill 50 ml centrifuge tubes to ~40 ml with RO water and apply sipper cap.
      
   2. Invert tubes and allow air bubble in sipper tube to rise.
      
   3. Make sure the water line is below the conical tapered end when inverted.
      
   4. Label each tube (e.g., “A” & “B” in permanent marker) and mark location of water line using a permanent marker.
      
   5. Alternatively, the initial bottle weight can be recorded.
      
   6. Place the 2 inverted tubes into wire lid, with minimal shaking to avoid dripping.
      
   7. Both bottles should be placed on one side of the divided wire rack, leaving the other side for food.
      
   8. Make sure that the rubber stopper is flushed with caging and that steel sipper tubes extend below wire cage lid (Figure 1).
      
   9. Avoid water leakage from sipper tubes when replacing cage on rack.
      
   10. Put food chow on the other side of the wire lid.
   Note: Ensure that bedding is not in excess. Mice can pile the bedding when nesting or if stressed, and bedding touching the sipper tube can cause the contents of the tube to empty. Alternatively, you may also add a “drip cage” to use as a control [for an example of this method see (Hwa et al., 2011)]. The drip cage is an empty cage that gets the same cage change and bottles daily. This sample drip loss can be subtracted from final calculations as an estimate of typical leakage.
   
   
   Figure 1. Picture of 2-bottle choice procedure setup in home cages. A. Sipper bottles separated out into its components consisting of metal sipper tube, rubber stopper (which the sipper tube is placed into via a hole in the center), and 50 ml conical centrifuge tube. B. Picture of 2-bottle setup in a home cage. The bottles are filled with solutions and place atop the wire mesh cage lid, with the metal sippers facing into the cage.
   
   
3. Assess baseline water consumption daily for 4 d. To assess consumption, weigh bottle or mark volume level.
   
   1. If conducting weight measurements, record pre- and post-consumption weights of the tube (1 g = 1 ml of water).
      
   2. For volume measurements, record volume levels on tube using a permanent marker.
      
   3. Different colored markers for each day are recommended.
      
   4. Do not invert tubes (where sipper cap is upright) when marking volume, as this allows air into the sipper and can cause dripping.
      
   5. Monitor for any problems with liquid flow and observe for signs of spillage, e.g., wet bedding, below the sipper tube.
      
   6. Switch positions (left vs right) of tubes daily.
4. Setup 2-bottle choice test for sucrose preference.
   
   1. Dissolve sucrose in RO water.
      
   2. Determination of sucrose concentration (% w/v; Figure 2) will require preliminary experiments using an initial dose-response curve (0.25-2%) to ascertain optimal sucrose preference necessary based on any a priori hypothesis.
      
   3.  For example, if your hypothesized outcome indicates a likely reduction in preference, a greater concentration is recommended. However, if you are expecting an increase in preference, lesser concentrations may be more appropriate.
      
   4. Fill one tube (e.g., one marked “A”) with fresh RO water and the other (“B”) with the sucrose solution. Place tubes on wire lid as previously described.
   
   
   Figure 2. An illustration of preference for sucrose in the 2-bottle choice test. A. Sucrose preference measured by raw volume consumed; B. Sucrose preference measured by % preference for sucrose.
   
   
5. Assess water and sucrose solution consumption daily for 4 d. Record weights and/or volume of each tube. Monitor for any problems with liquid flow or spillage, e.g., wet bedding, below the sipper tube. Switch positions (left vs right) of tubes daily.
   
6. Apply volume formula (see Notes) to determine consumption. Assess raw weight and/or volume consumed, and % preference for the sucrose-containing solution.

Notes

1. Side bias
   It is likely that some mice will develop bias for one side or the other, resulting in an increased consumption for one tube. Therefore, bottle positions within each cage are switched daily to avoid false sucrose preference resulting from side bias. Alternatively, if bias is a problem, tubes can be moved to the middle of the wire top and food chow placed on either side.
   
2. Volume formula
   Volume of liquid consumed can be determined based on vertical markings on the side of the cylinder. This derives from the tube dimensions and distance between daily marks, using the volume of a cylinder equation:
   V = π⋅ r² ⋅ h
   Where V = volume (in cm³, which is equivalent to ml), π ≈ 3.1416, r = radius (half the interior diameter in cm), and h = distance between daily markings (in cm). It is important to utilize only the cylindrical portions of the 50 ml tube, and avoid any fluid in the conical portion, as the volume formula differs there.
   
3. Animal considerations
   It is important to conduct preliminary studies in order to characterize the behavioral phenotype with particular equipment, environment, and animals. This is especially true in the case of varying mouse strains, either inbred or outbred, or if mice have been surgically or behaviorally manipulated prior to sucrose preference testing. All of these factors can affect baseline preference. In addition, some labs prefer to pre-handle mice for 5-7 d and singly house the animals for a period of 5-7 d prior to preference testing.
   

Acknowledgments

This behavioral procedure was adapted from previously published studies (Krishnan et al., 2007; Robison et al., 2014) and was performed by our group as described (Eagle et al., 2015). This work was supported by the Whitehall Foundation (AJR; 2013-08-43), the Multidisciplinary Training in Environmental Toxicology training grant (ALE; T32-ES007255), and a 2014 NARSAD Young Investigator Award from the Brain and Behavior Research Foundation (ALE).

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1. Eagle, A. L., Mazei-Robison, M. and Robison, A. J. (2016). Sucrose Preference Test to Measure Stress-induced Anhedonia. Bio-protocol 6(11): e1822. DOI: 10.21769/BioProtoc.1822.
   
2. Eagle, A. L., Gajewski, P. A., Yang, M., Kechner, M. E., Al Masraf, B. S., Kennedy, P. J., Wang, H., Mazei-Robison, M. S. and Robison, A. J. (2015). Experience-dependent induction of hippocampal DeltaFosB controls learning. J Neurosci 35(40): 13773-13783.